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Endocrinology, doi:10.1210/en.2005-0567
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Endocrinology Vol. 146, No. 12 5100-5111
Copyright © 2005 by The Endocrine Society

Sertoli Cell Expression of Steroidogenic Acute Regulatory Protein-Related Lipid Transfer 1 and 5 Domain-Containing Proteins and Sterol Regulatory Element Binding Protein-1 Are Interleukin-1ß Regulated by Activation of c-Jun N-Terminal Kinase and Cyclooxygenase-2 and Cytokine Induction

Tomomoto Ishikawa, Keumsil Hwang, Deborah Lazzarino and Patricia L. Morris

Center for Biomedical Research, The Population Council (T.I., K.H., D.L., P.L.M.), and Rockefeller University (P.L.M.), New York, New York 10021

Address all correspondence and requests for reprints to: Dr. Patricia L. Morris, Center for Biomedical Research, The Population Council and Rockefeller University, 1230 York Avenue, New York, New York 10021. E-mail: p-morris{at}popcbr.rockefeller.edu.


   Abstract
Top
 Abstract
Introduction
 Materials and Methods
 Results
 Discussion
 References
 
In testicular Sertoli cells, IL-1ß regulates steroid, lactate, and transferrin secretion; although each influences germ cell development and spermatogenesis, little is known about the signaling mechanisms involved. In other cell types, IL-1ß potently induces reactive oxygen species and/or cyclooxygenase-2 (COX-2). In contrast, in Sertoli cells, IL-1ß does not generate reactive oxygen species, but rapidly phosphorylates c-Jun-NH2-terminal kinase (JNK), but not p44/42 or p38 MAPK. Phosphorylated JNK stimulates COX-2 activity, mediating the expression of ILs and steroidogenic acute regulatory (StAR)-related (StAR-related lipid transfer protein domain containing) proteins D1 and D5, but not D4. In a time- and dose-dependent manner, IL-1ß rapidly increases levels of COX-2 mRNA (2-fold); induction of COX-2 protein (50-fold) requires de novo protein synthesis. Concomitantly, increases in IL-1{alpha}, IL-6, and IL-1ß mRNAs (1–3 h) are observed. As StAR-related lipid transfer protein domain containing protein 1 (StARD1) mRNA decreases, StARD5 mRNA increases; substantial recovery phase induction of StARD1 mRNA above control is noted (24 h). Inhibition of JNK or COX-2 activities prevents IL-1ß induction of IL and StARD5 mRNAs and subsequent increases in StARD1 mRNA (24 h), indicating that these effects depend on the activation of both enzymes. StARD1 and D5 protein levels are significantly altered, consistent with posttranscriptional and posttranslational regulation. IL-1ß rapidly decreases levels of precursor and mature sterol regulatory element-binding protein-1, changes not altered by cycloheximide, suggesting coordinate regulation of StARD1 and -D5, but not StARD4, expression. These data demonstrate that JNK and COX-2 activities regulate Sertoli cytokines and particularly START domain-containing proteins, suggesting protective stress responses, including transcription and protein and lipid regulation, within this specialized epithelium.


   Introduction
Top
 Abstract
 Introduction
Materials and Methods
 Results
 Discussion
 References
 
THROUGHOUT SPERMATOGENESIS, SIGNIFICANT interactions within the seminiferous tubule occur between the epithelial Sertoli cell (SC) and specific developing and maturing male germ cells. After mitosis and meiosis of germ cells, haploid spermatids differentiate during spermiogenesis, and the resulting sperm are released into the lumen to the efferent ducts. ILs play multiple interactive roles, both hormone dependent and independent, in the regulation and dysregulation of Sertoli function and male germ cell development. During Sertoli cell development and differentiated function, IL-1 and IL-6 are expressed under basal physiological conditions in response to the pituitary gonadotropic hormone FSH. These cytokines are also induced during the later stages of spermiogenesis when cytoplasm is shed from elongating spermatids as cytoplasts or residual bodies, subsequently undergoing phagocytosis by the surrounding SC. The presence of residual bodies in defined stages of the seminiferous cycle activates Sertoli phagocytosis and IL-1 release, events that initiate IL-6 secretion by an autocrine mechanism through the lipoxygenase pathway (1, 2, 3). This normal stage-specific process in the tubules induces SC cytokine production, including IL-1{alpha}, IL-1ß, and IL-6, and also accompanies pathological testicular inflammation (1, 2, 3, 4, 5, 6, 7). Stage-specific IL-1-like activity was found to stimulate DNA synthesis in mitotic spermatogonia and preleptotene spermatocytes, whereas IL-6 exerts the opposite effect (8, 9, 10). IL-1ß and IL-6 family members and their specific receptors are expressed in cell-specific patterns in the human, mouse, porcine, and rat testis, indicating their potential as paracrine factors to exert biological activity (7, 11, 12, 13, 14, 15, 16). In SC, IL-1ß has been shown to regulate estradiol, lactate, IL-6, and transferrin production and secretion, suggesting that this cytokine regulates diverse, but critical, autocrine and paracrine secretory factors (5, 17, 18, 19, 20, 21). However, to date, the molecular mechanisms subserving such effects within the seminiferous tubule are not well understood.

IL-1ß signaling involves multiple signal transduction pathways and numerous intracellular mediators, including the c-Jun N-terminal kinase (JNK), MAPK, p44/42 and p38 MAPK, and Akt/protein kinase B pathways (22, 23, 24, 25, 26, 27). In human astrocytes, vascular smooth muscle cells, and endothelial cells, IL-1ß cyclooxygenase (COX) induction was shown to be dependent on the activation of protein kinase C (28, 29). The inducible isozyme COX-2 is a protein whose expression and activity are induced by IL-1ß in specialized cell types and regulated during tissue development and remodeling (30, 31). Little is known about the functional consequence(s) of physiological COX activation in the testis. Using steroidogenic Leydig cell progenitors purified from the testis, we showed that acute treatment with IL-1ß is a potent inducer of the transient expression of several ILs, effects mediated by activation of the COX-2 pathway and induction of prostaglandin (PG) F2{alpha} and PGE2 production (24, 32). In such steroid-producing progenitors, the expression of steroidogenic acute regulatory protein [StAR; StAR-related lipid transfer protein domain containing protein 1 (StARD1)], the founding member of the StAR lipid transfer [StAR-related lipid transfer protein (START) domain] family of proteins, was unaffected by IL-1ß treatment or the induction of COX-2 and PG. In contrast, lipopolysaccharide-induced shock or the presence of inflammatory levels of cytokines, including IL-1ß, can decrease StAR and inhibit several steroidogenic enzymes in adult Leydig cells, leading to subsequent decline in testosterone and sperm production (33, 34, 35, 36, 37). Differences between these studies are probably due in part to the complex array and high levels of cytokines released in response to lipopolysaccharide.

Therefore, particular effects of IL-1ß are probably specified by the distinct testicular cell type and duration and degree of exposure: transient and within physiological levels, rapidly induced as a response to a stress, or released in a chronic, elevated manner during the development of inflammatory disease (27, 38). For this study, the specific kinetics and molecular mechanisms of IL-1ß signaling and intracellular regulation of the SC were investigated.


   Materials and Methods
Top
 Abstract
 Introduction
 Materials and Methods
Results
 Discussion
 References
 
SC preparations
SC were purified from the testes of 18-d-old Sprague Dawley [Crl: CD (Sprague Dawley) BR-CD] rats purchased from Charles River Laboratories, Inc. (Kingston, NY). Animals were housed in standard lighting (12 h of light, 12 h of darkness) and allowed food and water ad libitum. They were maintained in facilities approved by the American Association for the Accreditation of Laboratory Animal Care. Procedures involving the use of animals strictly followed the Guidelines for Care and Use of Laboratory Animals set forth by the National Institutes of Health and protocols received institutional animal care and use committee approval. Primary cultures (≥95% pure) were maintained at a density of 1 x 107 cells/100-mm polystyrene dish in phenol red-, serum-, and endotoxin-free DMEM/Ham’s F-12 medium (Irvine Scientific, Santa Ana, CA) at 34 C as described previously (11, 12). The medium was supplemented with 2.5 µg/ml bovine insulin (Sigma-Aldrich Corp., St. Louis, MO), 1 µg/ml transferrin (Calbiochem, La Jolla, CA), and 10 µg/ml bacitracin (Sigma-Aldrich Corp.). On d 3 ex vivo, SC were rinsed twice with fresh serum- and phenol red-free culture medium and then treated with IL-1ß (10 ng/ml) in the absence or presence of COX activity inhibitors, 1-(4-chlorobenzoyl)-5-methoxy-2-methyl-1H-indole-3-acetic acid (INDO; 10 µM; COX-1 and -2) or NS-398 (N-[2-(cyclohexyloxy)-4-nitrophenyl]-methanesulfonamide; 10 µM; COX-2 selective), and/or the JNK inhibitor, SP600125 [(N1-methyl-substituted pyrazolanthrone (N1-methyl-1, 9-pyrazoloanthrone)); 10 µM], or the protein synthesis inhibitor, cycloheximide (CHX; 5 µg/ml). At 1, 3, 6, and 24 h after vehicle, IL-1ß, or addition of the inhibitor(s), whole-cell lysates for protein and total RNA were isolated from each replicate. Duplicate or triplicate culture dishes were used for each drug treatment, and experiments were repeated at least twice. The mean (±SEM) of all the experiments was calculated for RNA analyses.

Drugs
Recombinant IL-1ß was purchased from R&D Systems, Inc. (Minneapolis, MN). NS-398 was purchased from Cayman Chemical Co. (Ann Arbor, MI). INDO and CHX were obtained from Sigma-Aldrich Corp. SP600125 was purchased from Calbiochem.

Recombinant IL-1ß was dissolved in 0.1% BSA in PBS as a 100-fold (10 µg/ml) stock solution. Matched aliquots of 0.1% BSA were used in control cultures; the final BSA concentration was 0.0001%. COX and JNK inhibitors were dissolved in dimethylsulfoxide (DMSO) and CHX was dissolved in absolute ethanol; subsequent dilutions, as needed, were performed in serum- and phenol red-free medium on the day of the experiment. DMSO alone and/or ethanol were used as matched vehicle controls in all plates as required. The final DMSO concentration was 0.1%.

Protein extraction and Western analysis
Whole-cell homogenates were extracted for protein lysates for 15 min on ice in buffer [10 mM Tris-HCl (pH 7.8) containing 1% Nonidet P-40, 0.1% sodium dodecyl sulfate, 150 mM NaCl, 1 mM EDTA, 1 mM phenylmethylsulfonylfluoride, 2 mM dithiothreitol, 2 mM sodium orthovanadate, 2 µg/ml aprotinin, 2 µg/ml pepstatin, and 2 µg/ml leupeptin]. Cellular debris was pelleted by centrifugation at 12,000 x g for 15 min.

The proteins in the supernatant were then subjected, under reducing conditions, to SDS-PAGE using 4–20% Tris-glycine gels (Novex, San Diego, CA), and were electrophoretically transferred to a nitrocellulose membrane (Schleicher & Schuell, Keene, NH). The membranes were probed with antibodies, as described below. Phospho-stress-activated protein kinase/JNK polyclonal antibody (pAb; 1:1000), phospho-MAPK pAb (1:1000), and phospho-p38 MAPK pAb (1:1000) were obtained from Cell Signaling Technology, Inc. (Beverly, MA). COX-2 pAb (1:1000) was obtained from Cayman Chemical Co. StARD1 pAb (1:2000) was obtained from Affinity BioReagents, Inc. (Golden, CO). StARD5 and StARD4 pAbs were provided by Dr. Jan Breslow (The Rockefeller University, New York, NY) (39). Sertoli sterol regulatory element-binding protein-1 (SREBP-1) pAb was obtained from Santa Cruz Biotechnology, Inc. (H-160; Santa Cruz, CA). Monoclonal anti-ß-actin antibody (1:2000) was purchased from Sigma-Aldrich Corp. Blots were developed with the ECL Western blotting system (Amersham Biosciences, Arlington Heights, IL) and exposed to x-ray film (Eastman Kodak Co., Rochester, NY). Densitometric analysis was performed using the personal computer version of National Institutes of Health Image software (Scion Image) after scanning. For Western analyses, particular signal intensities in each lane were normalized with those for ß-actin on the same membranes, and data are expressed as arbitrary units relative to control, set as a value of 1.

Total RNA extraction
Total RNA was extracted from SC using the TRIzol reagent (Invitrogen Life Technologies, Inc., Grand Island, NY) according to the manufacturer’s instructions. RNA was measured using 260/280 UV spectrophotometry.

RT-PCR analysis
Total RNA (2 µg) was reverse transcribed for 15 min at 42 C. RT was performed in a 20-µl mixture containing 5 mM MgCl2, 1x PCR buffer II, 4 mM each of deoxy-NTP, 1 U/µl ribonuclease inhibitor, and 2.5 mM random hexamers. Samples were then denatured for 5 min at 99 C. A no-template control was performed for each experiment, establishing the absence of genomic contamination of the samples. PCR was performed using 3 µl of each RT product as a template. The following primers were used: COX-2 sense primer, 5'-GGCCATGGAGTGGACTTAAA-3'; antisense primer, 5'-GGAACTGCTGGTTGAAAAGC-3' (442-bp product); and S16 ribosomal gene sense primer, 5'-TCCGCTGCAGTCCGTTCAAGTCTT-3'; antisense primer, 5'-GCCAAACTTCTTGGATTCGCAGCG-3' (385-bp product). AmpliTaq DNA polymerase (Applied Biosystems, Foster City, CA) was used at 25 mU/µl. The PCR mixture (25 µl) contained 2 mM MgCl2, 1x PCR buffer II, and each primer at 0.2 µM. Amplification was performed in a programmable thermal controller (model PTC-100, MJ Research, Inc., Watertown, MA). The samples were first denatured at 95 C for 2 min, followed by 30 PCR cycles; the temperature profile was 95 C (30 sec), 60 C (30 sec), and 72 C (1.5 min). After the last cycle, additional extension incubation at 72 C (7 min) was performed. After amplification, PCR products (5 µl of each sample) were subjected to size separation by polyacrylamide gel (4–20% Tris/boric acid/EDTA gels; Novex). The bands were visualized by UV fluorescence after staining with ethidium bromide (1 µg/ml) for 15 min. Densitometric analysis was performed using the personal computer version of National Institutes of Health Image software (Scion Image) after photography with a computer-assisted camera (Eastman Kodak Co.). COX-2 levels were normalized with S16 values and were expressed as arbitrary units relative to the control, set as a value of 1.

Real-time PCR analysis
Quantitative real-time fluorescence-monitored PCR (Q-PCR) assays using a standard curve method of analysis were conducted to quantitatively determine in each sample the levels of rat IL-1{alpha}, IL-1ß, IL-6, StARD1, and StARD5 mRNAs (6-carboxy-fluorescein-labeled probes) with 18S ribosomal RNA (VIC dye-labeled probe) used to normalize the data for specific mRNAs.

Reactions were set up in triplicate in optical 96-well reaction plates by adding 23 µl of a mix containing 1x Q-PCR Master Mix Plus (Eurogentec, Philadelphia, PA), 200 nM primers, 100 nM probe for the gene of interest, 50 nM primers, and 200 nM probes for the 18S ribosomal RNA, and 2 µl of 6-fold diluted cDNA sample was subsequently added to each well.

Detection of IL mRNAs was performed using proprietary TaqMan primers and probes (Applied Biosystems). StARD1, StARD4, and StARD5 primers were designed and prepared to order (Applied Biosystems) for this study: D1: forward, GCCCATGGACAGACTCTATGAAG; and reverse, TCCTTGACATTTGGGTTCCACT, with ACCGCATGGAGGCCATGGG as probe; D4: forward, ATGCGTTACACCACTGCTGG; and reverse, CTTCATAGCCCACAGTATAGGAGAAA, using CAGCTTTTAAATATTATTTCCCCGAGAGAGTTTGTTG as probe; and D5: forward, TGGCACCATCAGCTCCAAT; and reverse, TCTCACAAAACCGGGCTTTG, using CCCATGTGGAACATCCATTGTGTCCC as probe.

Q-PCRs were performed using a PE Applied Biosystems model 7700 Sequence Detection System. The temperature profile for the reactions was 50 C (2 min), 95 C (10 min), and for 40 cycles at 95 C (15 sec) and 60 C (1 min). Using the manufacturer’s software, a threshold above the noise was chosen, and the cycle number at which fluorescence, generated by the cleavage of the probe, exceeded the threshold was determined for each well. For each real-time PCR assay, a standard curve was generated by six 2-fold serial dilutions in water of the RT samples corresponding to the 1-h treatment of SC with IL-1ß. The mean threshold cycle value for each cDNA sample was expressed as an arbitrary value relative to the standard curve after linear regression analysis. A no-template control was performed for each reaction in duplicate. Data were normalized with 18S values and were expressed as arbitrary units relative to the control, set as a value of 1.

Bioimaging
Primary SC were isolated from rat testes, purified, and maintained (3 d, 34 C) in 35-mm, glass-bottom culture dishes (MatTek, Ashland, MA). SC were then treated with IL-1ß for 3 h, placed on ice, and fixed (15 min) with 2% paraformaldehyde. Fixed cells were washed well with PBS and then permeabilized with 1 ml 0.1% IGEPAL CA630 detergent (Sigma-Aldrich Corp.) in PBS (15 min at room temperature). Free aldehyde groups were quenched by incubation with 0.1 M glycine in PBS (15 min at room temperature). Nonspecific binding was blocked by incubation of cells in PBS with 10% normal goat serum in PBS (blocking buffer; 30 min at room temperature). To double label the cells, rabbit antisera directed against StARD1 and StARD5 were preincubated with Alexa Fluor 488- and Alexa Fluor 594-conjugated rabbit IgG labeling reagents, respectively, according to the manufacturer’s protocol (Zenon Tricolor Rabbit IgG Labeling Kit, Molecular Probes, Inc., Eugene, OR). For the negative control, antibody complexes were prepared using normal rabbit IgG (Upstate Biotechnology, Inc., Lake Placid, NY) as the primary antibody. The ratio of labeling reagent to primary antibody was 6:1; final complexes were combined and diluted to a 1:90 final concentration in blocking buffer. Cell monolayers were incubated with 50 µl antibody mixtures in a humidified chamber (30 min at room temperature), then washed with blocking buffer. SC nuclei were stained using 4,6-diamino-2-phenylindole (DAPI) (Sigma-Aldrich Corp.; 4 µg/ml; 5 min) and rinsed in PBS before mounting in ProLong Antifade (Molecular Probes, Inc.), which was applied to the glass bottom, with a second coverglass used to seal the well. Images were captured using an inverted Axiovert 200 laser scanning microscope LSM510 confocal analyzer (Carl Zeiss, New York, NY) equipped with a UV laser, and a krypton/argon laser with 488- and 568-nm lines and a helium-neon laser with 633-nm line, allowing excitation of green-, red-, and far red-emitting fluorochromes and multitrack scanning fluorescence.

Flow cytometry
The fluoroprobe, 5-(and 6)-chloromethyl-2', 7'-dichlorodihydrofluorescein diacetate (CM-H2-DCFDA) was used to measure reactive oxygen species (ROS) in SC after treatment with inflammatory stimuli. This probe diffuses passively through the cellular membrane and is retained after intracellular deacetylation by endogenous esterases. The thiol-reactive chloromethyl group reacts with intracellular glutathione and other thiols. Upon oxidation, the fluorescent product dichlorofluorescein (DCF) is produced. On d 3, SC were preloaded with CM-H2-DCFDA (8 µM) for 30 min, then maintained for various times (2.5, 5, 10, 15, 20, 30, and 60 min) with IL-1ß, IL-6, vehicle (negative control), or 0.03% hydrogen peroxide (H2O2; positive control) at 34 C in 5% CO2. Cell samples were washed and resuspended in PBS, and cell-associated fluorescence intensity was measured using a FACSCalibur cytometer (BD Biosciences, San Jose, CA).

Data analysis
Densitometric analyses are expressed in arbitrary units. All results are the mean ± SEM derived from the number of different experiments. Statistical analyses were performed using t test or paired t test and ANOVA. P ≤ 0.05 was considered significant.


   Results
Top
 Abstract
 Introduction
 Materials and Methods
 Results
Discussion
 References
 
The following experiments were conducted using primary SC to determine the intracellular targets of IL-1ß signaling responsible for changes in specific gene expression and biochemical processes. Because IL-1ß has been shown to activate JNK and ROS in certain cell types, we first sought to determine whether these signaling components were activated in SC (26, 28, 40).

IL-1ß activates phosphorylation of SC JNK
Proteins were isolated from whole-cell lysates of SC treated with IL-1ß as indicated. Western analyses showed a doublet of phosphorylated JNK (phospho-JNK2/3 and phospho-JNK1; 54 and 46 kDa, respectively) within 30 min (Fig. 1AGo), but not p44/42 or p38 MAPK, Akt, or JAK2 kinases (data not shown). Each membrane was reprobed for ß-actin to determine equal loading in the lanes and for normalization of particular signals. IL-1ß significantly activated JNK1 and JNK2/3 by serine phosphorylation as demonstrated (i.e. at 30 min, a 4.1-fold increase compared with control; P < 0.001; Fig. 1BGo). Treatment with the JNK-specific inhibitor SP600125 (10 µM) blocked IL-1ß-induced phospho-JNK (Fig. 2AGo).



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  		FIG. 1. IL-1ß activates phosphorylation of SC JNK. SC cultured in the presence or absence (control, Ct) of IL-1ß (10 ng/ml) for various periods of time. A, Western analysis using whole-cell extracts showed a phosphorylated JNK protein doublet (54 and 46 kDa) within 30 min of the addition of IL-1ß; the same membrane was reprobed for ß-actin (42 kDa) to determine equal loading in the lanes and for normalization of signals. B, Densitometric analysis was performed. Phosphorylated JNK results are normalized with ß-actin values and are expressed as arbitrary units relative to control (Ct), set at a value of 1. A representative experiment of three replicates is shown in A and B. Results are the mean ± SEM. ***, Significant difference (P < 0.001) from the value for control cultures treated only with vehicle blank (Ct).

 


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  		FIG. 2. The JNK activity inhibitor SP600125 decreases IL-1ß induction of Sertoli cell phospho-JNK and COX-2 protein levels, but does not stimulate intracellular ROS formation. A, SC were cultured for 30 min with IL-1ß (10 ng/ml) in the absence (DMSO vehicle blank; lane 1) or presence of SP600125 (10 µM; lane 2). Western analysis using whole-cell extracts showed a down-regulation of phosphorylated JNK protein doublet (54 and 46 kDa) 30 min after the addition of SP600125; the same membrane was reprobed for ß-actin (42 kDa) to determine equal loading in the lanes and for normalization of signals. B, Primary SC isolated from immature rats were cultured for 3 d as described. On d 3, SC were preloaded with CM-H2-DCFDA (8 µM) for 30 min, then maintained for various times with IL-1ß, IL-6, vehicle (negative control), or 0.03% hydrogen peroxide (H2O2; positive control) at 34 C in 5% CO2. Cell samples were washed and resuspended in PBS, and cell-associated fluorescence intensity was measured using a BD Biosciences FACSCalibur cytometer. Results are shown for the 30 min point for IL-1ß and IL-6 treatments. Each panel contains histogram overlays of H2O2 control (bold solid line), vehicle alone (dotted line), and cytokine (thin solid line) treatments. C, SC were cultured for 1 and 3 h with IL-1ß (10 ng/ml) in the absence (DMSO vehicle blank; lanes 1 and 2) or presence of SP600125 (10 µM; lanes 3 and 4). Western analysis using whole-cell extracts showed a down-regulation of COX-2 protein (72 kDa) after the addition of SP600125; the same membrane was reprobed for ß-actin (42 kDa) to determine equal loading in the lanes and for normalization of signals.

 
IL-1ß does not stimulate intracellular ROS formation in SC
The balance of overall ROS production in response to acute cytokine exposure or an inflammatory challenge with H2O2 was determined using a reactive chemical probe, CM-H2-DCFDA. Cytometric excitation and measurement of DCF were used to analyze the changes in overall cell-associated ROS in SC in response to cytokine exposure. The oxidative stress response after treatment with IL-1ß was compared with those of IL-6 and H2O2. Primary SC, cultured for 3–4 d in serum-free medium, were assayed for cellular respiratory burst in response to treatment with 10 ng/ml IL-1ß or IL-6 for periods of 2.5–60 min. For control conditions, similar cells were treated in parallel with the appropriate vehicle for each cytokine mixture as a negative control or with H2O2 (0.03%) as a positive indicator of the overall cellular oxidative response. Treatment with H2O2 resulted in a robust signal increase for oxidative burst, as measured by fluorescence DCF probe. Interestingly, SC did not increase ROS production in response to either IL-1ß (Fig. 2BGo, upper panel) or IL-6 (Fig. 2BGo, lower panel). In fact, the response to IL-1ß was less than the vehicle control for all time points tested, indicating reduced basal intracellular ROS levels. Such findings support an antiinflammatory role for IL-1ß signaling in SC.

We next determined the kinetics and dose dependency of SC COX-2 induction by IL-1ß activation of JNK.

IL-1ß induces SC COX-2 and requires JNK activation
JNK phosphorylation was required for the increases observed in IL-1ß-inducible COX-2 protein [Fig. 2CGo, lane 1 vs. 3 (1 h) and lane 2 vs. 4 (3 h)]. To determine whether IL-1ß regulates COX-2 transcription, RT-PCR analyses were performed using total RNA extracts (three replicates) obtained from multiple primary SC experiments. COX-2 mRNA levels significantly increased in response to IL-1ß as early as 3 h (1.7-fold over control; P < 0.01) and remained significantly elevated at similar levels for 24 h or more after IL-1ß addition (P < 0.01; Fig. 3AGo). Steady-state S16 RNA levels were used for normalization.



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  		FIG. 3. IL-1ß induces SC COX-2 expression and de novo synthesis of COX-2. SC were cultured in the presence or absence (control, Ct) of IL-1ß (10 ng/ml) for various periods of time; for each of three experiments, total RNA and whole-cell protein extracts were prepared from replicates. A representative experiment is shown in B and D. Results are the mean ± SEM. ***, P < 0.001; *, P < 0.05 (significant difference from the Ct value). A, RT-PCR analyses for COX-2 mRNA levels were normalized with S16. Densitometric analysis is shown. {cjs2108}, Vehicle control; {blacksquare}, IL-1ß treated. B, Western analyses detects the induction of the 72-kDa COX-2 protein; the same membrane shown was reprobed for ß-actin (42 kDa) levels to determine protein loading in each lane. C, Densitometric analysis. COX-2 levels are normalized to ß-actin values and are expressed in arbitrary units, with Ct set at 1. D, SC were pretreated with vehicle blank or CHX (5 µg/ml, 30 min), and then treated with IL-1ß (10 ng/ml, 6 h). Lane 1, IL-1ß plus vehicle; lane 2, IL-1ß plus CHX. Inhibition of new protein synthesis by CHX eliminated IL-1ß-induction of COX-2 protein.

 
To ascertain whether increased JNK or COX-2 activity is directly involved in IL-1ß-induced effects on COX-2 mRNA, SC were treated with IL-1ß for 3 h in the absence (DMSO vehicle blank) or presence of the COX inhibitors, INDO (10 µM) and NS-398 (10 µM), or the JNK inhibitor, SP600125 (10 µM). Neither inhibition of COX-2 activity by INDO nor NS-398 pretreatment itself significantly decreased IL-1ß-induced COX-2 mRNA levels. SP600125 significantly, albeit modestly, decreased IL-1ß-induced COX-2 mRNA levels (0.84-fold; P ≤ 0.04), findings consistent with the involvement of the JNK pathway in the 2-fold induction of COX-2 mRNA by IL-1ß (Fig. 3AGo). COX-1 remained constitutively expressed, but unchanged (data not shown).

To more fully evaluate the effects of IL-1ß on COX-2 induction at the level of its translation and steady-state protein levels in SC, Western blot analyses were performed. A time-dependent IL-1ß induction of COX-2 protein was demonstrated (Figs. 2CGo and 3Go, B and C). Significant induction of COX-2 protein was first evident within 1 h of treatment and was elevated more than 20-fold by 3 h. Strikingly, IL-1ß-stimulated 50-fold increases in COX-2 protein levels at 6 h (Fig. 3CGo; P < 0.001). Given that IL-1ß induced COX-2 mRNA levels 2-fold, these data are consistent with two different, but complementary, IL-1ß mechanisms of action, one transcriptional and the second a potent translational and/or posttranslational effect.

Stimulation of COX-2 protein requires de novo protein synthesis
To determine the mechanisms for induction of COX-2 expression by IL-1ß, SC were pretreated with the protein synthesis inhibitor, CHX (30 min). CHX prevented the IL-1ß induction of COX-2 protein (Fig. 3DGo), indicating that IL-1ß induction of COX-2 protein requires de novo protein synthesis. After CHX and IL-1ß treatment, no significant change was seen in the constitutive levels of COX-1 protein (data not shown).

Previous studies from this laboratory and others have indicated that physiological and proinflammatory cytokine factors may play a role in the paracrine and autocrine regulation and dysregulation of SC paracrine function. Therefore, we next examined the effect of IL-1ß on levels of SC cytokine expression.

Concomitant IL-1ß induction of IL expression occurs in a time- and dose-dependent manner
IL-1{alpha}, IL-1ß, and IL-6 mRNAs were evaluated by Q-PCR analyses using sets of matched RNA replicates from five different experiments. IL-1{alpha} (5.6-fold; Fig. 4AGo) and IL-6 (2.8-fold; Fig. 4CGo) mRNAs were significantly induced by IL-1ß by 1 h (P < 0.001), a time at which no increase in IL-1ß mRNA was observed (Fig. 4BGo). At 6 h, levels of IL-1{alpha}, IL-6, and IL-1ß mRNAs increased 9.4-, 3.3-, and 12.7-fold, respectively, above control levels (P < 0.001; Fig. 4Go). To examine the dose-response effect of IL-1ß on IL-1{alpha}, IL-1ß, and IL-6 expression, SC were treated with or without IL-1ß at various doses (0.1, 1, 10, and 100 ng/ml) for 3 and 6 h. At both 3 and 6 h, IL-1ß induced the mRNA for each of these cytokines in a dose-dependent manner (Fig. 5Go).



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  		FIG. 4. IL-1ß induces the expression of IL-1{alpha}, IL-1ß, and IL-6 mRNAs in a time-dependent manner. SC were cultured without (control, Ct) or with IL-1ß (10 ng/ml) for the indicated times. Total RNAs were extracted, and cDNAs were amplified using Q-PCR using specific primers and probes for IL-1{alpha} (A), IL-1ß (B), or IL-6 (C). Results are the mean ± SEM. Data are normalized with 18S values and are expressed relative to Ct, set at 1. **, P < 0.01; ***, P < 0.001 (significant difference from the Ct value).

 


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  		FIG. 5. IL-1ß induces the expression of IL-1{alpha}, IL-1ß, and IL-6 mRNAs in a dose-dependent manner. SC were cultured without (control, Ct) or with IL-1ß at the indicated doses for 3 and 6 h. Total RNAs were extracted, and cDNAs were amplified by Q-PCR using specific primers and probes for IL-1{alpha} (A), IL-1ß (B), or IL-6 (C). Results are the mean ± SEM. Data are normalized with 18S values and are expressed with Ct at 1.

 
To determine whether activation of COX was required for these changes in cytokine expression, the effects of both COX activity inhibitors on IL-1ß-mediated regulation of IL-1{alpha}, IL-1ß, and IL-6 mRNA levels were examined.

COX and JNK activity inhibitors decrease IL-1ß induction of SC IL-1{alpha}, IL-1ß, and IL-6 mRNAs
In contrast to the failure of the COX activity inhibitors to affect IL-1ß induction of COX-2 mRNA levels, as early as 1 h the dual COX-1/COX-2 activity inhibitor INDO did significantly reduce, in part, the IL-1ß-stimulated increases in IL-6 mRNA, but not those in IL-1{alpha} or IL-1ß (data not shown). This inhibition was maintained at 3 h (2.9-fold; P < 0.001, compared with IL-1ß and vehicle; Fig. 6Go, E and F). For 3 and 6 h, the NS-398-specific inhibitor of COX-2 activity significantly decreased IL-1ß induction of IL-1{alpha} (1.5- and 1.9-fold, respectively; Fig. 6Go, A and B), IL-1ß (1.8- and 2.6-fold; Fig. 6Go, C and D), and IL-6 (3.9- and 2.8-fold; Fig. 6Go, E and F) mRNA levels (Fig. 6Go, B, D, and F; P < 0.001). Similar to those effects observed with INDO treatment, NS398 significantly decreased IL-1ß-induction of IL-6 mRNA as early as 1 h. Therefore, the early-onset changes in IL-6 expression are dependent on rapid changes in COX activity.



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  		FIG. 6. COX and JNK activities mediate IL-1ß-induction of SC IL-1{alpha}, IL-1ß, and IL-6 expression. SC were cultured for 3 and 6 h without (control, Ct) or with IL-1ß (10 ng/ml) in the absence (DMSO vehicle blank, Veh) or presence of INDO (10 µM), NS-398 (10 µM), or SP600125 (10 µM). Q-PCR for IL-1{alpha} (A and B), IL-1ß (C and D), or IL-6 (E and F) were performed using the same RT. Results are the mean ± SEM. Data are normalized with 18S values and are expressed with Ct set at 1. *, P < 0.05; **, P < 0.01; ***, P < 0.001 [significant difference from the IL-1ß response (Veh+)].

 
The JNK inhibitor SP600125 did significantly reduce, in part, IL-1ß-stimulated increases in IL-1{alpha} and IL-6 mRNAs, but not those in IL-1ß, effects observed as early as 3 h (Fig. 6Go, A, C, and E). At 6 h, SP600125 significantly inhibited IL-1ß induction of IL-1{alpha} (1.7-fold; Fig. 6BGo) and IL-1ß (3.7-fold; Fig. 6DGo) mRNA levels (P < 0.05 and P < 0.001, respectively). NS398 plus SP600125 treatment completely inhibited the IL-1ß-stimulated increases in IL-1ß and IL-6 by 6 h (Fig. 6Go, D and F). In comparison, the elevated level of IL-1{alpha} mRNA was significantly abrogated (Fig. 6BGo).

To determine whether the IL-1ß-induction of SC COX, JNK, and cytokine pathways were associated with endoplasmic reticulum (ER) stress or intracellular lipid trafficking (41), we next evaluated the expression of several START domain-containing proteins. The expression of StARD5 (ER stress regulated) and StARD4 (cholesterol) were first determined in SC, then compared with that of a known START domain protein, StAR (D1; cAMP regulated) (39, 42).

IL-1ß regulates SC StARD1 and StARD5 mRNAs and proteins, but not StARD4
StARD1, StARD4, and StARD5 mRNA levels were evaluated by Q-PCR analyses using sets of matched RNA replicates from five different primary experiments (i.e. SC isolated and purified from 40 testes in each experiment). In contrast to the induction of cytokines, IL-1ß significantly decreased StARD1 mRNA as early as 1 h (Fig. 7AGo, {blacksquare}; 0.7-fold; P < 0.001) as StARD5 mRNA levels increased (Fig. 7AGo,

{cjs2113}

; 1.6-fold; P < 0. 01). At 6 h, a significant reduction in StARD1 mRNA levels (0.5-fold; P < 0.001) was still consistently observed; the StARD5 mRNA level was now not significantly different from the control level. Interestingly, in each experiment our data indicate that a subsequent and significant increase in StARD1 mRNA beyond the matched control steady-state level occurs 24 h after the addition of IL-1ß (1.7-fold; P < 0.05). After IL-1ß treatment, no changes were observed in StARD4 mRNA levels (Fig. 7AGo, {square}).



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  		FIG. 7. IL-1ß treatment of the SC leads to rapid decreases in their StARD1 concomitant with increases in StARD5 mRNA and protein levels. SC were cultured without (control, Ct) or with IL-1ß (10 ng/ml) for various periods of time. A, Total RNAs were extracted, and cDNAs were amplified by Q-PCR using specific primers and probes for StARD1 ({blacksquare}), StARD4 ({square}), and StARD5 ({cjs2113}). Results are the mean ± SEM. Data are normalized with 18S values and are expressed with Ct at 1. *, P < 0.05; **, P < 0.01; ***, P < 0.001 (significant difference from the Ct value). B, A representative Western analysis using whole-cell extracts illustrates time course-related changes in steady-state levels of StARD1 (30–32 kDa) and StARD5 (28 kDa) proteins after IL-1ß (10 ng/ml); the same membrane was reprobed for StARD4 (not shown) and ß-actin.

 
Western analyses showed that increased total cellular levels of the mature 30-kDa and intermediate 32-kDa StARD1 proteins occurred as early as 1–3 h; both forms were significantly decreased at 6 h (Fig. 7BGo). In contrast to StARD1, the 28-kDa StARD5 protein decreased as early as 30 min and remained significantly decreased at very low, but detectable, levels from 1–6 h (Fig. 7BGo). Taken together, cellular StARD5 levels indicate that IL-1ß-induced changes in transcription are accompanied by a significant posttranslational effect(s), i.e. on its half-life, or degradation. No changes in StARD4 protein levels were observed (data not shown).

Bioimaging of StARD1and StARD5
On d 3 ex vivo, SC were treated for 3 h without (Fig. 8Go, A–C) or with IL-1ß (10 ng/ml; Fig. 8Go, D–F). SC were double immunolabeled with anti-StARD1 and anti-StARD5 antibodies. To facilitate the use of two pAb for a double-labeling protocol, Fabs of anti-Fc antibodies coupled to Alexa Fluor 488 and 594 (Molecular Probes, Inc.) fluorochromes were employed. As a control for nonspecific binding, we also double labeled with nonimmune rabbit IgG that was complexed separately with both fluorophores. For both antibody reagents, the nonspecific controls gave little to no background labeling (Fig. 8Go, H and I). StARD1 was localized in the perinuclear regions of the monolayer epithelial SC, but we did not observe any apparent changes in the pattern of localization induced by IL-1ß (Fig. 8Go, B and E). Based on fluorescent labeling, StARD5 was diffusely distributed in the cytoplasm compared with StARD1. Qualitatively, fluorescent levels of intracellular StARD5 decreased dramatically. These bioimaging findings are consistent with decreases measured quantitatively for whole-cell StARD5 protein using Western analysis, which show a dramatic decline 3 h after the addition of IL-1ß.



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  		FIG. 8. Confocal microscopic analyses of SC StARD1 and StARD5 after IL-1ß treatment. On d 3 ex vivo, SC were treated for 3 h with either vehicle as an untreated negative control (Ct; A–C) or IL-1ß (10 ng/ml; D–F). SC were double immunolabeled with a combination of anti-StARD1-Alexa Fluor 488 (green) and anti-StARD5-Alexa Fluor 594 (red) antibody complexes (A–F) or with normal rabbit IgG antibody labeled with both Alexa Fluor reagents (negative control; G–I). Confocal images were acquired using an inverted Zeiss Axiovert 200 microscope with a x63 oil objective and filter sets for DAPI, fluorescein isothiocyanate, and Cy3. In each row, left panels show the DAPI (nuclear) signal (A, D, and G), center panels show the anti-StARD1 (B, E, and H), and right panels show the anti-StARD5 signal (C, F, and I).

 
IL-1ß-stimulated COX-2 and JNK activities are required for regulation of StARD5 and recovery phase increases in StARD1 mRNAs
INDO, NS-398, and SP600125 treatment failed to inhibit the IL-1ß-mediated reductions in StARD1 mRNA levels at 3 and 6 h (not shown), but inhibitors of JNK and COX activities blocked the IL-1ß-induced secondary increases in StARD1 mRNA consistently observed at 24 h (Figs. 7AGo and 9AGo, {blacksquare}). In contrast to StARD1, NS-398 did inhibit the IL-1ß-mediated inductions in StARD5 mRNA levels at 3 h (Fig. 9BGo), consistent with COX regulation of D5 transcription. Taken together, these data suggest that although the initial IL-1ß-mediated inhibition of StARD1 transcription is not dependent on COX activity, the subsequent recovery phase StARD1 increases are COX dependent.



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  		FIG. 9. COX activity inhibitors, INDO and NS-398, and JNK inhibitor, SP600125, inhibit IL-1ß-induced increases in StARD1 mRNA at 24 h. SC were cultured for 3, 6, and 24 h without (control, Ct) or with IL-1ß (10 ng/ml) and in the absence (vehicle blank, Veh) or presence of INDO (10 µM), NS-398 (10 µM), or SP600125 (10 µM). Q-PCR analyses for StARD1 (A, 24 h) and StARD5 (B, 3 h) mRNAs are shown; data represent the mean of triplicate determinations ± SEM. StARD1 and StARD5 data are normalized with those for 18S and are expressed relative to Ct, set at 1. *, P < 0.05; **, P < 0.01; ***, P < 0.001 [significant difference from the IL-1ß response (Veh+)].

 
IL-1ß changes in SREBP-1 are COX-2 and JNK activity dependent
To better evaluate the regulation of these START domain proteins, we next studied the effects of IL-1ß on SREBP-1. The cellular levels of both the precursor and mature SREBP-1 (125 and 68 kDa, respectively) proteins decreased rapidly with time after IL-1ß treatment (Fig. 10Go, lanes 2–5). In the presence of either the inhibitor of COX-2 (lanes 6–9) or JNK (not shown) activities, the IL-1ß-induced decline in SREBP-1 levels was truncated; SREBP-1 levels recovered to control levels as early as 3 h (Fig. 10Go, lane 8). CHX pretreatment had no effect on the IL-1ß-induced decreases in either the precursor or mature SREBP-1 (not shown). These findings are consistent with posttranslational mechanisms for the SREBP-1 transcription factor.



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  		FIG. 10. IL-1ß decreases intracellular Sertoli SREBP-1 proteins, decreases abrogated by NS398 treatment. SC were treated for the indicated times without (Ct; lane 1) or with IL-1ß (10 ng/ml) in the absence (DMSO vehicle blank; lanes 2–5) or presence of NS398 (10 µM; lanes 6–9) for the times indicated. Western analysis using whole-cell extracts showed down-regulation of both SREBP-1 precursor (125 kDa) and mature (68 kDa) proteins after NS398 addition; the same membrane was reprobed for ß-actin.

 

   Discussion
Top
 Abstract
 Introduction
 Materials and Methods
 Results
 Discussion
References
 
In epithelial SC, the present data show that IL-1ß activates JNK1 and JNK2/3 by phosphorylation, a kinase activation that is required for the induction and activation of the COX-2 enzyme. These findings are in agreement with those using renal mesangial and endothelial cells, but not other kinases for immune and other diverse cell types (25, 43, 44, 45). In SC, inhibition of JNK decreases both IL-1ß-induced phosphorylation of JNK and increases in the levels of COX-2 mRNA and protein, findings consistent with our proposal that JNK activity regulates the inducible form of COX. COX-2 induction requires transcription and de novo protein synthesis. These findings suggest that transient exposure to locally produced IL-1ß can stimulate the Sertoli COX-2 cascade in an autocrine manner. Neither IL-1ß nor IL-6 treatment increased ROS production. Moreover, IL-1ß could provide a protective antioxidant-like effect, resulting in decreased basal ROS levels compared with either control or IL-6-treated levels. A working model based on these current findings is illustrated (Fig. 11Go). By altering the seminiferous tubule microenvironment through COX-2-mediated changes in SC secretions such as PGs and cytokines, the potential exists for secondary, specific paracrine effects on germ cells. The data provide additional evidence that IL-1ß is a potent transcriptional autocrine regulator of SC, inducing the expression of several cytokines (IL-1{alpha}, IL-1ß, and IL-6) in a time- and dose-dependent manner. These data suggest an important regulatory role for p54 and p46 JNK and the COX-2 cascade pathways in the control of cytokine production within the seminiferous tubule.



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  		FIG. 11. JNK Serves as a SC molecular switch for intracellular signaling and processes. A proposed model illustrates the effects of IL-1ß signaling on SC autocrine and paracrine activities.

 
Copeland et al. (46) reported that INDO and NS-398 bind to the active sites of COX-1 and COX-1 and -2, respectively, subsequently causing a slow, irreversible event with significant enzymatic inactivation. Neither had an effect on COX-2 transcription or COX-2 mRNA steady-state levels, but they did block COX-regulated PG production. In this study, early-onset changes in IL-6, but not in IL-1{alpha} or IL-1ß, expression are dependent on the activity of the COX-2 enzyme.

In contrast to our study with steroidogenic Leydig progenitors showing that the addition of IL-1ß and COX-2 activation of PG production had no direct effect on StAR expression (24), using age-matched, but fully differentiated, epithelial SC, IL-1ß significantly decreased StARD1 mRNA levels as early as 1 h. This inhibition was sustained at 6 h, but was followed by a subsequent and significant recovery phase increase in StAR mRNA beyond control steady-state levels (24 h). Differences in the regulatory mechanisms in distinct cell types are suggestive of specific feedback mechanisms defined by cell type as well as function. In the testis, the adult Leydig cell exhibits the most abundant expression of StARD1 commensurate with its ability to respond to the pituitary gonadotropin, LH, with cAMP-dependent StAR-mediated acute mitochondrial transfer of cholesterol to accumulate at the P450 side-chain cleavage site of action. Both posttranslational processing of the preexisting 37-kDa StAR to the intermediate 32- and mature 30-kDa forms for cholesterol transfer and new synthesis of the StARD1 protein are required (47, 48, 49). Previous studies demonstrated StAR protein in human and rodent SC and its induction in immature rat primary SC in response to stimulation by the gonadotropin FSH or a cAMP analog (50, 51). However, its precise role in this specialized epithelial cell remains largely unknown.

To our knowledge, this study shows for the first time the expression of two additional START domain-containing proteins, StARD4 and StARD5, in epithelial SC. Sertoli StAR and StARD5 proteins are differentially regulated by IL-1ß, but StARD4 is not. StARD5 mRNA levels increased with IL-1ß treatment as early as 1 h compared with concomitant decreases in StARD1 mRNA. Although little is known about the regulation of StARD5, the pattern of its expression indicates that it may be regulated by ER stresses, functioning as a sensor and mediator for the intracellular shuttling of sterols or other lipids (39). Interestingly, the bioimaging of the two START domain proteins also demonstrated somewhat different cellular patterns of localization. In SC, StARD1 protein is localized in perinuclear regions of the monolayer epithelial SC, a common pattern consistent with mitochondrial localization, whereas StARD5 was diffusely distributed in the cytoplasm. Consistent with our expression data, no apparent change was observed in the overall immunodetectable pattern of StARD1 between the control and IL-1ß-treated cells at 3 h. Because the ratios of the two forms of StAR did not change during this time, and the antibody recognizes both forms, the Western and intracellular immunodetection findings are consistent. Also, in agreement with multiple sequential D1 and D5 Western analyses from replicate experiments, StARD5 protein was significantly decreased in IL-1ß-treated SC to barely detectable levels compared with the uniformly distributed and relatively abundant D5 levels in matched control cells. StARD5 mRNA levels were not transiently induced in IL-1ß-treated SC in which COX-2 and JNK activities were also inhibited, indicating a requirement for kinase and COX activities. At 6 h, levels of StARD5 protein remained significantly below those in vehicle-matched control cells. Together, these findings indicate a role for COX-2 activity and the products of this pathway in StARD5 expression and homeostasis.

Cholesterol homeostasis is finely regulated in all cells to ensure an adequate intracellular supply and lipid homeostasis while avoiding excessive accumulation (52). Much of this regulation is transcriptional and mediated by members of the SREBP family of transcription factors that control cholesterol and lipid homeostasis (53, 54). However, it is likely that cholesterol regulation in the testis reflects a high degree of cell specificity at the transcriptional level. For example, the lack of a coordinate transcriptional control over the cholesterol biosynthetic pathway contributes importantly to overproduction of the signaling sterol testis meiosis-activating sterol (T-MAS) in the testis (55).

Recent studies identified transcriptional and posttranscriptional regulation of specific genes by cholesterol- and isoprenoid-derived signaling molecules (reviewed in Ref.54). In addition, the metabolic pathways in which these signaling molecules participate may exert important regulatory influences on the SC, which regulate the developing germ cells within the seminiferous tubule. Whether the observed decline in immunodetectable StARD5 is due to a combination of posttranscriptional and posttranslational effects, such as a failure to properly fold and/or protect the protein from degradation, requires additional study. However, it is likely that specific StARD5 protein function is compromised. For example, proper protein folding regulates the StAR-like steroidogenic function of the START domain-containing protein MLN64 (metastatic lymph node 64) (56, 57). Additionally, a recent study showed that NIH-3T3 fibroblast cells treated with tunicamycin to induce ER stress had 6- to 8-fold increases in StARD5 mRNA levels (39). Regulation of Sertoli START domain protein function may represent fine-tuning of metabolic processes and gene expression directly or may indirectly affect spermatogenesis by altering the Sertoli secretory microenvironment of developing germ cells and differentiating sperm.

Changes in StAR transcription and/or mRNA stability are known to be important regulatory events in the functional response of steroidogenic cells to hormone action (58). The StAR gene controls the rate-limiting step in the biogenesis of steroid hormones, delivery of cholesterol to the cholesterol side-chain cleavage enzyme on the inner mitochondrial membrane (47). Transcriptional regulation of the StAR gene is under basal regulation by steroidogenic factor-1 and is acutely regulated by hormones through the functional involvement of a cAMP response element-binding protein (59, 60). Recent studies identified histone modifications associated with active transcription and gene silencing in the control of StAR gene expression (61). Analysis of the human and rodent StARD1 promoter indicates that SREBP-1 enhances StAR transcription, but is unaffected when mature SREBP levels are suppressed (62, 63, 64).

SREBPs are bound to ER membranes until their cleavage by an SREBP cleavage-activating protein (SCAP), an event that requires new transcription of SCAP (65, 66). SREBP-1 (125 kDa) is bound in a hairpin fashion, and when proteolytically released from the membrane, the released NH2-terminal domain (68 kDa) is a transcription factor of the basic-helix-loop-helix-leucine zipper family, which then enters the nucleus. SREBP-regulated genes are involved not only in the synthesis of cholesterol, fatty acids, triglycerides, low-density lipoprotein receptor, and reduced nicotinamide adenine dinucleotide phosphate, but also in the synthesis of phospholipids (67). In the present studies, cellular levels of both the precursor and mature SREBP-1 decreased rapidly, findings coincident with the decline in StARD1 mRNA levels. The COX-2 specific activity inhibitor or the JNK inhibitor, which subsequently blocked induction of COX-2 RNA and protein, truncated this decrease in SREBP-1 and shortened the recovery to control levels. Induction of COX-2 in SC leads to marked deceases in the endoplasmic membrane 125-kDa SREBP-1, with a concomitant decline in the 68-kDa transcription factor. Transcription-dependent SCAP degradation of SREBP precursor and coactivators have been shown to be feedback mechanisms to regulate the expression of genes involved in cholesterol metabolism and may also regulate the duration of such transcriptional responses through protein stability (68, 69, 70). To date, our findings indicate that the effect of IL-1ß on endogenous SREBP-1 is due in part to posttranscriptional mechanisms.

Known SREBP target genes show coordinate regulation (39). In contrast to StARD4, the expression of START domain-containing family members MLN64 and StARD5 do not appear to be sterol regulated (39, 42, 52). However, overexpression of both StARD4 and StARD5 does stimulate liver X receptors reporter activity, suggesting their roles in cholesterol metabolism (39). In SC, decreases in both SREBP-1 forms were temporally associated with rapid induction of StARD5 mRNA at a time when D5 protein decreased to almost undetectable levels. Such IL-1ß-induced changes are indicative of transcriptional regulation of StARD5 as well as posttranscriptional effects. Temporally the effects on D5 were the inverse of those on D1, i.e. StARD1 mRNA levels strikingly decrease whereas the 32 ≥ 30-kDa forms of mature StAR increase markedly, effects consistent with posttranslational processing. Although the effects of IL-1ß on SREBP-1 may directly affect StARD1 promoter activity (62, 63, 71), concomitant changes in D5 expression may be SREBP-1 independent, because StARD5 is transcriptionally activated by ER stressors (39, 52). Proper protein folding appears to regulate StAR-like steroidogenic function of MLN64 (56, 57). Taken together, these data indicate that noninflammatory IL-1ß activation of signaling mediated by COX-2, JNK phosphorylation, reduced intracellular ROS, and induction of IL-1{alpha}, IL-6, and StARD5 transcription may reflect early-stage responses of the SC to ER stress, coordinated responses that together protect this cell. The absence of changes in StARD4 expression is consistent with studies that indicate it is regulated by sterols and SREBP2 transcriptional activation, but not by ER stress (39).

In summary, the present study indicates that specific Sertoli StAR-related (START) domain-containing proteins and cytokines are regulated by IL-1ß using mechanisms involving the activation of JNK and inducible COX-2 pathways, with effects on SC gene and protein expression within the seminiferous tubule (proposed model, Fig. 11Go). In addition, the present findings may be relevant to physiological role(s) for distinct START domain-containing proteins in intracellular sterol or lipid trafficking or metabolism by specialized epithelial cells in other organs.


   Acknowledgments
 
We express our appreciation for the excellent cell handling skills and technical assistance of Lyann Mitchell, and the editorial assistance of Jean Schweis. Dr. Alison North, Director of the Rockefeller University Bio-Imaging Resource Center, provided expertise and assistance with confocal microscopy. The use of The Population Council’s cell biology and flow cytometry facility is gratefully acknowledged.


   Footnotes
 
This work was supported by National Institutes of Health Grants HD-29428 and HD-39024 (to P.L.M.).

First Published Online August 25, 2005

Abbreviations: CHX, Cycloheximide; CM-H2-DCFDA, 5-(and 6)-chloromethyl-2', 7'-dichlorodihydrofluorescein diacetate; COX, cyclooxygenase; DAPI, 4,6-diamino-2-phenylindole; DCF, dichlorofluorescein; DMSO, dimethylsulfoxide; ER, endoplasmic reticulum; INDO, 1-(4-chlorobenzoyl)-5-methoxy-2-methyl-1H-indole-3-acetic acid; JNK, c-Jun NH2-terminal kinase; MLN64, metastatic lymph node 64 protein; pAb, polyclonal antibody; PG, prostaglandin; Q-PCR, quantitative real-time PCR; ROS, reactive oxygen species; SC, Sertoli cell; SCAP, sterol regulatory element-binding protein cleavage-activating protein; SREBP-1, sterol regulatory element-binding protein-1; StAR, steroidogenic acute regulatory protein; StARD1, StAR-related lipid transfer protein domain containing protein 1; START, StAR-related lipid transfer protein.

Received May 11, 2005.

Accepted for publication August 17, 2005.


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Top
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 Introduction
 Materials and Methods
 Results
 Discussion
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